bioRxiv preprint doi: https://doi.org/10.1101/753525; this version posted September 4, 2019. The copyright holder for this preprint (which was not certified by peer review) is the author/funder, who has granted bioRxiv a license to display the preprint in perpetuity. It is made available under aCC-BY-NC-ND 4.0 International license.
1 Understanding and eliminating the detrimental effect of endogenous thiamine
2 auxotrophy on metabolism of the oleaginous yeast Yarrowia lipolytica
3
4 Caleb Walker,1,§ Seunghyun Ryu,1,§ Richard J. Giannone,2 Sergio Garcia,1 Cong T. Trinh1,*
5 1Department of Chemical and Biomolecular Engineering, The University of Tennessee Knoxville,
6 TN 37996
7 2Chemical Sciences Division, Oak Ridge National Laboratory, Oak Ridge, TN 37831
8
9 §Equal contributions
10 *Corresponding author
11 Email: [email protected]
12 Tel: 865-974-8121
13
14
15
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bioRxiv preprint doi: https://doi.org/10.1101/753525; this version posted September 4, 2019. The copyright holder for this preprint (which was not certified by peer review) is the author/funder, who has granted bioRxiv a license to display the preprint in perpetuity. It is made available under aCC-BY-NC-ND 4.0 International license.
16 ABSTRACT
17 Thiamine is an essential vitamin that functions as a cofactor for key enzymes in carbon and energy
18 metabolism for all living cells. While most plants, fungi and bacteria can synthesize thiamine de
19 novo, the oleaginous yeast, Yarrowia lipolytica, cannot. In this study, we used proteomics
20 together with physiological characterization to understand key metabolic processes influenced
21 and regulated by thiamine availability and identified the genetic basis of thiamine auxotrophy in
22 Y. lipolytica. Specifically, we found thiamine depletion results in decreased protein abundance
23 of the lipid biosynthesis pathways and energy metabolism (i.e., ATP synthase), attributing to the
24 negligible growth and poor sugar assimilation observed in our study. Using comparative
25 genomics, we identified the missing gene scTHI13, encoding the 4-amino-5-hydroxymethyl-2-
26 methylpyrimidine phosphate synthase for the de novo thiamine synthesis in Y. lipolytica, and
27 discovered an exceptional promoter, P3, that exhibits strong activation or tight repression by low
28 and high thiamine concentrations, respectively. Capitalizing on the strength of our thiamine-
29 regulated promoter (P3) to express the missing gene, we engineered the first thiamine-
30 prototrophic Y. lipolytica reported to date. By comparing this engineered strain to the wildtype,
31 we unveiled the tight relationship linking thiamine availability to lipid biosynthesis and
32 demonstrated enhanced lipid production with thiamine supplementation in the engineered
33 thiamine-prototrophic Y. lipolytica.
34
35 IMPORTANCE
36 Thiamine plays a crucial role as an essential cofactor for enzymes in carbon and energy
37 metabolism of all living cells. Thiamine deficiency has detrimental consequences on cellular
2
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38 health. Yarrowia lipolytica, a non-conventional oleaginous yeast with broad biotechnological
39 applications, is a native thiamine auxotroph, whose effects on cellular metabolism are not well
40 understood. Therefore, Y. lipolytica is an ideal eukaryotic host to study thiamine metabolism,
41 especially as mammalian cells are also thiamine-auxotrophic and thiamine deficiency is
42 implicated in several human diseases. This study elucidates the fundamentals of thiamine
43 deficiency on cellular metabolism of Y. lipolytica and identifies genes and novel thiamine-
44 regulated elements that eliminate thiamine auxotrophy in Y. lipolytica. Furthermore, discovery
45 of thiamine-regulated elements enables development of thiamine biosensors with useful
46 applications in synthetic biology and metabolic engineering.
47
48 Keywords: Yarrowia lipolytica; thiamine metabolism; thiamine auxotroph; thiamine prototroph;
49 thiamine-regulated promoters; lipid production; thiamine deficiency
50
51
52
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53 INTRODUCTION
54 Thiamine, or vitamin B1, was the first B vitamin discovered. Its activated form, thiamine
55 pyrophosphate (TPP), functions as a cofactor for key enzymes in carbon metabolism including
56 glycolysis, citrate cycle, pentose phosphate and branched chain amino acid pathways (Figure 1)
57 (1). TPP-dependent enzymes, including pyruvate dehydrogenase (PDH), α-ketoglutarate
58 dehydrogenase (KGDH), transketolase (TKL), branched chain α-ketoacid dehydrogenase (BCKDC)
59 and acetolactate synthase (AHAS), are essential for maintaining cell growth and preventing
60 metabolic stress (2, 3). Specifically, PDH links the glycolysis and citrate (Krebs) cycle by catalyzing
61 the conversion of pyruvate into acetyl-CoA (4)(5). KGDH, the rate-limiting step of the citrate
62 cycle, converts α-ketoglutarate to succinyl-CoA (6, 7). TKL is responsible for the last step of the
63 pentose phosphate pathway where it interconverts pentose sugars to glycolysis intermediates
64 (8). The pentose phosphate pathway is critical for production of ribose (i.e., RNA), precursor
65 metabolites for aromatic amino acid pathways, and reducing equivalents (i.e., NADPH) necessary
66 for maintaining redox balance and lipid synthesis. Hence, TKL activity is critical for RNA, protein,
67 and lipid production while preventing oxidative stress (9, 10). Meanwhile, AHAS and BCKDC are
68 responsible for the synthesis and degradation of branched chain amino acids (i.e., valine, leucine
69 and isoleucine), respectively (11)(12).
70 In mammals, thiamine deficiency affects the cardiovascular and nervous systems resulting
71 in tremors, muscle weakness, paralysis and even death (13)(14). Thiamine deficiency can occur
72 from inadequate intake, increased requirement, or impaired absorption of thiamine (15).
73 Biochemical consequences of thiamine deficiency result in failure to produce adenosine
74 triphosphate (ATP), increased acid production (i.e., lactic acid), decreased production of acetyl-
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75 compounds (i.e., acetylcholine), neurotransmitters (i.e., glutamate, aspartate, aminobutyric
76 acid), reduced nicotinamide adenosine dinucleotide phosphate (NADH), defective ribonucleic
77 acid (RNA) ribose synthesis, and failure to break down branched chain carboxylic acids (i.e.,
78 leucine, valine, isoleucine)(16-18).
79 While mammals require nutritional supplementation of thiamine from dietary sources,
80 most bacteria, fungi and plants can synthesize thiamine endogenously. One of these exceptions
81 is the thiamine-auxotrophic oleaginous yeast, Yarrowia lipolytica, which has recently emerged as
82 an important industrial microbe with broad biotechnological applications due to its GRAS status
83 (19), metabolic capability (20-24), and robustness (25-27). Hence, Y. lipolytica is an ideal
84 eukaryotic host to study the fundamental effects of thiamine deficiency on cellular health.
85 Currently, it is not well understood why thiamine deficiency causes failure of thiamine
86 biosynthesis in Y. lipolytica and how this deficiency might directly affect other processes (e.g.,
87 lipid biosynthesis, energy metabolism, etc.) beyond what is already known.
88 Interestingly, Y. lipolytica’s auxotrophy has been exploited for enhanced production of
89 organic acids (i.e., pyruvate and KGA) by reducing activities of PDH and KGDH under thiamine-
90 limited conditions (28, 29). Consequently, cell growth is negatively affected by thiamine
91 limitation and completely prevented when thiamine is depleted from the media. Not
92 surprisingly, the genes in thiamine metabolism are tightly regulated by thiamine concentrations
93 (30, 31). To this end, numerous thiamine-regulated promoters have been discovered in yeast
94 that enable control of genetic expression by adjusting thiamine concentration in the culture
95 media (32-34). However, endogenous thiamine-regulated promoters have not yet been
5
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96 discovered in Y. lipolytica. Furthermore, fundamental understanding of how thiamine deficiency
97 inhibits metabolism and hence growth of Y. lipolytica is still lacking.
98 In this study, we shed light on the effect of thiamine deficiency on cellular metabolism in
99 the thiamine auxotroph Y. lipolytica. We identified the missing gene, scTHI13, in the de novo
100 thiamine biosynthesis pathway of Y. lipolytica and discovered a thiamine-regulated promoter,
101 P3, that increases expression in low thiamine concentrations. By employing P3 to control the
102 expression of scTHI13, we engineered thiamine prototrophy for the first time in Y. lipolytica. This
103 enabled us to elucidate the relationship between thiamine availability and ATP and lipid
104 biosynthesis and revealed enhanced lipid production in the engineered thiamine-prototrophic Y.
105 lipolytica.
106
107 RESULTS
108 The effects of thiamine deficiency in Y. lipolytica
109 Cell growth and organic acid production are influenced by thiamine limitation and
110 depletion. To demonstrate the effects of thiamine limitation, we characterized the thiamine-
111 auxotrophic Y. lipolytica (YlSR001) in 0, 0.5 and 400 µg/L thiamine (Figure 2A). As expected, cell
112 growth was inhibited by limited (0.5 ug/L thiamine) and depleted (0 ug/L thiamine)
113 concentrations of thiamine but restored in high thiamine (400 ug/L thiamine) containing media
114 (Figure 2B). Glucose consumption profiles were closely coordinated with cell growth (Figure 2C).
115 Within the first 24 hr, only ~2 g/L glucose was assimilated without thiamine while thiamine-
116 limited cultures consumed ~3 g/L glucose (Figure 2C). After 24 h, growth and glucose
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117 consumption were completely stalled under the no thiamine condition. In contrast, cells
118 continued to utilize glucose even though growth was significantly inhibited.
119 Next, we characterized pyruvate and KGA production since the enzymes converting these
120 organic acids, PDH and KGDH respectively, are TPP-dependent. In high thiamine media, Y.
121 lipolytica demonstrated slight KGA production (~0.5 g/L KGA) and no pyruvate accumulation
122 (Figure 2D, 2E). Not surprisingly, we observed substantial pyruvate titers in thiamine limited (~4
123 g/L pyruvate) and depleted (~2 g/L pyruvate) media (Figure 2E) as PDH is unable to efficiently
124 convert pyruvate to acetyl-CoA. Similarly, KGA accumulation was enhanced in thiamine-limited
125 media (2 g/L KGA) but KGA titers in thiamine-depleted media were comparable to high thiamine
126 media likely due to decreased flux from glycolysis to the TCA cycle through deficient acetyl-CoA
127 production via PDH (Figure 2D). Taken together, Y. lipolytica requires thiamine supplementation
128 for cell growth and carbon assimilation but produces organic acids under thiamine-limited
129 conditions.
130 Proteome of thiamine depletion reveals perturbation of critical metabolic pathways
131 related to cellular growth. Next, we investigated the proteome of the thiamine-auxotrophic Y.
132 lipolytica growing in 0 and 400 µg/L thiamine (Figure 3A). Across 2 exponential time points, we
133 identified 535 upregulated and 515 downregulated proteins (i.e., log2 fold change > |1|) in
134 response to thiamine deficiency (Figure 3B). First, we looked at metabolic enzymes that require
135 TPP as a cofactor including PDH, KGDH, transketolase (TKL), branched chain α-ketoacid
136 dehydrogenase (BCKDC) and acetolactate synthase (AHAS) (Supplementary Table S1).
137 Interestingly, all proteins encoding subunits (E1-E3) of BCKDC were upregulated in thiamine
138 depletion (Supplementary Table S1). However, none of the other TPP-requiring proteins were
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139 upregulated in media lacking thiamine except for dihydrolipoamide dehydrogenase (E3), which
140 serves as a subunit for BCKDC, PDH and KGDH (Supplementary Table S1).
141 We then mapped the 535 upregulated- and 515 downregulated proteins to their
142 respective KEGG pathways (Figure 3C). Thiamine deficiency resulted in downregulation of
143 proteins involved in nucleic acid metabolism (i.e., pyrimidine and purine metabolism) and genetic
144 processes (i.e., ribosome and DNA replication). Without thiamine, cells also exhibited decreased
145 protein abundance in lipid metabolism which includes the synthesis of terpenoids, steroids and
146 glycerophospholipids. In contrast, thiamine deficiency resulted in upregulation of proteins
147 contained in carbohydrate (i.e., glycolysis and citrate cycle), tetrapyrrole, biotin, aromatic (i.e.,
148 tryptophan, phenylalanine), branched chain (i.e., leucine, isoleucine, valine), and other amino
149 acid (i.e., glycine, serine, threonine) metabolic pathways. Thiamine deficiency also affected
150 proteins associated with the electron transport chain (ETC), amino acid (i.e., arginine, proline,
151 glutamate, glutamine, methionine, cysteine) biosynthesis and thiamine metabolic pathways.
152 A closer look at proteins involved in the ETC and thiamine metabolism revealed
153 interesting features. First, thiamine-deficient cells exhibited increased protein abundances for all
154 four complexes of the ETC but decreased protein abundance for ATP synthase that is important
155 for ATP generation (Figure 3D). The phenomenon correlates with the stalled assimilation of
156 glucose that is ATP-dependent when cells grow in the absence of thiamine. Second, all but one
157 of the proteins in thiamine metabolism were differentially regulated between thiamine-sufficient
158 and thiamine-depleted cultures (Figure 3E). Without thiamine, we observed increased
159 abundance of proteins in the upper branch of thiamine synthesis but decreased abundance in
160 proteins converting thiamine monophosphate into thiamine and TPP into thiamine triphosphate.
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161 The only detected protein in thiamine metabolism that was not differentially translated was
162 thiamine kinase (Thi90p), which is responsible for the conversion of thiamine into its activated
163 diphosphate form, TPP. Taken together, thiamine concentration influences regulation of
164 thiamine metabolism, whereby thiamine deficiency severely affects central carbon metabolism
165 and elicits increased protein abundance for most carbohydrate, amino acid and energy pathways
166 but decreased protein abundance for lipid metabolism, nucleotide metabolism and specifically,
167 ATP synthase.
168 Restoring thiamine prototrophy in Y. lipolytica
169 Thiamine metabolism in Y. lipolytica is incomplete. Next, we investigated the native
170 thiamine metabolism of Y. lipolytica to elucidate underlying genetic deficiency causing thiamine-
171 auxotrophic behavior. We compared the thiamine biosynthesis pathways between the well-
172 characterized thiamine-prototrophic Saccharomyces cerevisiae and our thiamine-auxotrophic Y.
173 lipolytica. Between the two organisms, only one missing gene was identified (scTHI13), encoding
174 4-amino-5-hydroxymethyl-2-methylpyrimidine phosphate synthase that converts histidine and
175 pyrodixine into hydroxymethylpyrimidine pyrophosphate (HMP-PP), which is likely required for
176 the de novo thiamine synthesis in Y. lipolytica (Figure 3E).
177 Constitutive expression of the missing thiamine gene does not effectively restore
178 prototrophy. To enable the de novo biosynthesis of thiamine in Y. lipolytica, we constructed a
179 vector to express scTHI13 under the constitutive promoter, TEF, frequently used for genetic
180 overexpression in Y. lipolytica. Unexpectedly, expression of scTHI13 with the TEF promoter only
181 restored the de novo TPP biosynthesis after days of adaptation in thiamine-depleted media
182 (Supplementary Figure S1). Additionally, cell growth was highly deviated between replicates for
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183 both times when this experiment was conducted (Supplementary Figure S1). Though the results
184 were somewhat promising, we endeavored to engineer a true thiamine-prototrophic Y. lipolytica.
185 Bioinformatics of thiamine-responsive genes reveals highly regulated thiamine
186 promoter. We hypothesized that expression of scTHI13 was weak since the constitutive TEF
187 promoter (35, 36) is dependent on cell growth (37, 38) and thiamine deficiency prevents cell
188 growth. To this end, we aimed to find a promoter responsive to thiamine deficiency. Through
189 BlastP and orthology analysis using the well-studied thiamine-regulated genes from Pichia
190 pastoris, Saccharomyces cerevisiae and Schizosaccharomyces pombe, we identified three
191 candidate genes that are putatively regulated by thiamine in Y. lipolytica (Supplementary Table
192 S2). The P1 gene (YALI0E04224g) encodes a putative thiaminase that might exhibit
193 hydroxymethylpyrimidine kinase/phosphomethylpyrimidine kinase activity for conversion of
194 thiamine into 4-amino-5-hydroxymethyl-2-methylpyrimidine diphosphate. The P3 gene
195 (YALI0A09768g) encodes a putative cysteine-dependent adenosine diphosphate thiazole
196 synthase that is involved in the biosynthesis of thiazole, a thiamine precursor. Thiazole synthase
197 converts NAD+ and glycine into ADP-5-ethyl-4-methylthiazole-2-carboxylate, a thiazole
198 intermediate. Though the function of P2 (YALI0C14652g) has yet to be characterized, it harbors
199 a NMT1 domain (Pfam:PF09084) which is required for biosynthesis of the pyrimidine moiety of
200 thiamine (39); hence, P2 might be thiamine-regulated.
201 To determine if these promoters (i.e., P1, P2, and P3) are thiamine-regulated, real-time
202 PCR was conducted to quantify mRNA levels of P1, P2, and P3 genes from YlSR001 grown in low
203 (0.5 µg/L) and high (500 µg/L) concentrations of thiamine (Figure 4A). The expression levels of P1
204 and P3 genes were activated in low thiamine but inactivated in high thiamine. Remarkably, P3
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205 exhibited substantially increased expression relative to P1 by 7.60 ± 1.51-fold in low thiamine.
206 We did not observe transcriptional expression of P2 in low or high thiamine concentrations.
207 We next investigated plasmid expression of these 3 putative thiamine-regulated
208 promoters from the Y. lipolytica strains that harbor a humanized renilla green fluorescent protein
209 (hrGFP)-expressing gene under the control of either P1, P2, or P3 promoter (strains YlSR1002,
210 YlSR1003 and YlSR1004, respectively). For controls, we also built the native, constitutive TEF
211 promoter and the heterologous NMT1 promoter from S. pombe that has been well-studied and
212 applied as a thiamine-regulated promoter (40). The hrGFP intensity was monitored from cells
213 grown at low (1 µg/L) and high (10 mg/L) concentrations of thiamine (Figure 4B). As expected,
214 both P1 and P3 promoters were activated in low thiamine and inactivated in high thiamine.
215 Under low thiamine conditions, the hrGFP intensity under promoter P3 was exceptionally higher
216 than P1 and TEF promoters by 10.04 ± 0.46-fold and 2.82 ± 0.13-fold, respectively. Not
217 surprisingly, the activity of TEF promoter was much greater in high thiamine than in low thiamine.
218 The NMT1 promoter, however, showed no activity in low thiamine and limited activity in high
219 thiamine.
220 We further investigated the sensitivity of the P3 promoter over a range of low thiamine
221 concentrations (0.5-50 µg/L) (Figure 4C). Encouragingly, the P3 promoter exhibited tight
222 regulation across all incremental thiamine concentrations. Of note, the activity of the P3
223 promoter was not affected by cell growth (Figure 4D). Taken together, these data indicate that
224 the endogenous thiamine-regulated promoters, P1 and P3, can be applied to strain engineering
225 efforts and are responsive to low thiamine concentrations.
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226 Thiamine prototrophy is restored with thiamine regulated promoter. To restore the de
227 novo thiamine synthesis in Y. lipolytica, we constructed the vector pSR075 to express the missing
228 thiamine gene, scTHI13, with the thiamine-responsive promoter, P3 (i.e., YlSR1006). Remarkably,
229 this construct demonstrated robust and reproducible growth in media lacking thiamine (Figure
230 5). Cell growth and glucose uptake were similar despite with low to no added thiamine (Figure
231 5A, 5B), but organic acid production was affected. Organic acid production in low (0.5 µg/L) and
232 depleted (0 µg/L) thiamine conditions was diminished during the stationary phase (Figure 5C,
233 5D). Meanwhile, KGA accumulation only manifested in high (400 µg/L) thiamine (Figure 5C).
234 Taken together, the thiamine prototroph strain created here, YlSR1006, grows reproducibly
235 irrespective of thiamine concentrations but produces no organic acids in thiamine-limited media.
236 Lipid accumulation is influenced by thiamine concentrations. Finally, we investigated
237 the relationship between thiamine availability and lipid accumulation. We cultured both
238 thiamine-auxotrophic (wildtype) and our engineered thiamine-prototrophic (YlSR1006) strain
239 with 0 g/L and 400 g/L thiamine in MpA (no nitrogen limitation, Figure 6A) and lipid production
240 (nitrogen limitation with C:N = 100, Figure 6B) media. In non-nitrogen limited media, YlSR1006
241 produced more lipid than the wildtype grown with 400 g/L thiamine supplementation (Figure
242 6A). Interestingly, YlSR1006 grown without thiamine accumulated lipid similar to the wildtype
243 with 400 g/L thiamine. However, under nitrogen-limitation, both the wildtype and YlSR1006
244 strains showed similar lipid production profiles when 400 g/L thiamine was supplemented in
245 growth medium (Figure 6B). In thiamine-lacking medium, while no lipid accumulation was
246 expected for the wildtype, YlSR1006 was able to accumulate 3.68 ± 0.22 lipid %DCW, which was
247 ~50% less than YlSR1006 supplemented with 400 µg/L thiamine. Taken together, thiamine
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248 supplementation increased lipid production even for thiamine-prototroph YlSR1006, indicating
249 thiamine plays a critical role for lipid biosynthesis in Y. lipolytica.
250 DISCUSSION
251 In this study, we observed the effects of thiamine deficiency on growth, sugar
252 consumption, organic acid production, and proteome of the thiamine-auxotrophic Y. lipolytica.
253 The activated form of thiamine, TPP, is an important cofactor for enzymes involved in vital cellular
254 functions including energy metabolism (41), reducing oxidative and osmotic stresses (42), and
255 catabolism of sugars (43). Hence, the consequences of thiamine deficiency are caused by the
256 reduced activity of TPP-dependent enzymes (i.e., PDH, KGDH, TKL, AHAS and BCKDC), which
257 ultimately leads to cell death. A comprehensive model that depicts the detrimental effect of
258 thiamine deficiency on metabolism leading to cell death in Y. lipolytica is summarized in Figure
259 7.
260 Loss of PDH and KGDH activities result in poor growth, limited carbon assimilation and
261 accumulation of pyruvate and KGA (Figure 2). Failure to metabolize pyruvate via PDH also inhibits
262 production of acetyl-CoA, the precursor metabolite of the TCA cycle. The TCA cycle is further
263 inhibited by reduced KGDH activity, preventing synthesis of NADH required for oxidative
264 phosphorylation (i.e., ETC). Notably, in the model yeast, Saccharomyces cerevisiae, deletion of
265 KGDH is known to prevent respiratory growth (44), but the exact mechanism is not well
266 established. In our study, proteomic analysis shows that thiamine-deficient cells increased
267 protein abundance for the first four complexes of oxidative phosphorylation (i.e., NADH
268 dehydrogenase, succinate dehydrogenase, and cytochrome c reductase/oxidase) but decreased
269 protein abundance for ATP synthase (Figure 3D).These new findings indicate that thiamine
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270 deficiency negatively affects respiratory energy metabolism caused by a malfunctioning TCA
271 cycle via inhibition of PDH and KGDH as observed by inhibited growth and reduced sugar uptake
272 in thiamine-depleted cells.
273 Y. lipolytica also decreased protein abundances in glycerophospholipid, terpenoid
274 backbone and sterol biosynthesis pathways in thiamine-deficient cells (Figure 3C). These
275 phenomena are likely consequences of reduced PDH activity (i.e., reduced pools of acetyl-CoA)
276 and likely affected by NADPH production by the pentose phosphate pathway. In the pentose
277 phosphate pathway, TKL interconverts pentose sugars and hexose sugars, the later which serve
278 as glycolytic intermediates (e.g., fructose-6P, glyceraldehyde-3P). Hence, loss of TKL activity
279 likely effects the production of ribose-5P and NADPH which are required for synthesis of lipids,
280 RNA, DNA, purines, pyrimidines, and antioxidants (45). Interestingly, loss of TKL activity also
281 prevents production of erythrose-4P, impeding synthesis of folate and aromatic amino acids (i.e.,
282 phenylalanine, tyrosine, and tryptophan) as previously observed in TKL-deletion mutants of S.
283 cerevisiae (46).
284 In our study, Y. lipolytica also responded to thiamine deficiency by increasing protein
285 abundance of enzymes involved in branched chain α-amino acid metabolism (i.e., valine, leucine
286 and isoleucine). Consistent with the previous studies with S. cerevisiae, deletion of BCKDC results
287 in branched chain α-amino acid auxotrophic phenotypes (47). Interestingly, BCKDC was the only
288 TPP-requiring enzyme with all 3 subunits upregulated in our thiamine-depleted Y. lipolytica cells.
289 However, this finding might be the result of leucine supplementation in the media since our Y.
290 lipolytica strain is leucine auxotrophic. Taken together, thiamine deficiency inhibited cell growth
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291 severely limiting energy production, amino acids (i.e., aromatic and branched chain) and lipid
292 synthesis, ultimately leading to cell death (Figure 7).
293 Despite thiamine-mediated growth inhibition, Y. lipolytica exhibited strong upregulation
294 of proteins contained within thiamine metabolism in response to thiamine depletion (Figure 3E).
295 Interestingly, one of the enzymes upregulated in thiamine depletion, cysteine-dependent
296 adenosine diphosphate thiazole synthase (YALI0A09768g), is promoted by our thiamine-
297 regulated promoter, P3. While various constitutive and inducible promoters are available for Y.
298 lipolytica (48-51), our tightly regulated, thiamine-responsive P3 promoter is especially useful for
299 strong, inducible expression in low thiamine conditions. Under optimized conditions, the activity
300 of pP3 was 2.82 ± 0.13-fold higher than TEF (Figure 4B). Hence, gene overexpression using the
301 P3 promoter is highly desirable over the constitutive TEF promoter in low thiamine
302 concentrations. This was demonstrated by restoring thiamine prototrophy in Y. lipolytica using
303 P3 promoter (Figure 5), while the TEF promoter was not strong enough to accomplish stable
304 thiamine prototrophy (Supplementary Figure S1).
305 Surprisingly, thiamine prototroph was restored by overexpressing 1 single gene, absent
306 from the native metabolism of Y. lipolytica, for the de novo synthesis of thiamine (Figure 3E,
307 Supplementary Figure S1). This begs the question, why does Y. lipolytica lack this gene? We
308 hypothesize that most Y. lipolytica strains are isolated from thiamine-rich sources (e.g., sausage,
309 oats, plants) (52) while most popular yeasts, including S. cerevisiae, are isolated from sugar-rich
310 sources (e.g., fruits, molasses, sugarcane) (52). Remarkably, we observed enhanced lipid
311 production by thiamine supplementation in both thiamine-auxotrophic and prototrophic strains,
312 suggesting a relationship between lipid production and thiamine availability (Figure 6A, 6B). This
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313 relationship shows promise for industrial applications of neutral lipid production and establishes
314 a novel direction for increasing lipid production in Y. lipolytica.
315
316 MATERIALS AND METHODS
317 Plasmids and strains
318 The list of plasmids and strains used in this study is available in Supplementary Table S3.
319 Plasmid pSR005 carrying a humanized renilla green fluorescent protein (hrGFP) was constructed
320 by Gibson assembly method (53) with hrGFP and pSL16-CEN1-1-227 (54). The hrGFP gene was
321 amplified using the primers hrGFP_Fwd and hrGFP_Rev from pBABE GFP (Addgene plasmid
322 #10668). The backbone pSL16-CEN1-1-227 was amplified with the primers pSL16_Fwd and
323 pSL16_Rev.
324 Next, various promoters, TEF(404) (50), NMT1 (55), P1(1000), P2(1000), and P3(1000)
325 were inserted into pSR005 by Gibson assembly method. Each TEF(404), P1(1000), P2(1000), and
326 P3(1000) promoter region (size of each promoter is in parenthesis) was amplified using the
327 primers PTEF_Fwd/PTEF_Rev, PP1_Fwd/PP1_Rev, PP2_Fwd/PP2_Rev, and PP3_Fwd/PP3_Rev,
328 respectively from the genomic DNA of Y. lipolytica ATCC MYA-2613. The NMT1 promoter region
329 was amplified using the PNMT1_Fwd/PNMT1_Rev primers from the genomic DNA of S. pombe (kindly
330 provided by Dr. Paul Dalhaimer, Department of Chemical and Biomolecular Engineering,
331 University of Tennessee Knoxville, TN, USA). The backbone pSR005 was amplified by using the
332 primers pSR005_Fwd/pSR005_Rev. The constructed plasmids are pAT32y, pSR068, pSR071,
333 pSR072, and pSR073 (Supplementary Table S3).
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334 The plasmid pSR074 was constructed by assembly of (i) THI13sce, amplified using the
1 335 primers THI13sce_Fwd /THI13sce_Rev from the genomic DNA of S. cerevisiae and (ii) pSR008
336 backbone, amplified using the primers pSR008_Fwd/pSR008_Rev. The plasmid pSR075 was
337 constructed by replacing the hrGFP gene with the THI13sce gene from pSR073. The THI13sce
2 338 gene was amplified by using the primers THI13sce_Fwd /THI13sce_Rev from the genomic DNA of
339 S. cerevisiae and assembled with the PP3 promoter carrying backbone, amplified by using the
340 primers pSR008_Fwd/pSR073_Rev.
341 The Y. lipolytica ATCC MYA-2613, obtained from ATCC strain collection, was used as a
342 parent strain. YlSR101, YlSR109, YlSR1001 and-YlSR1006 (Supplementary Table S3) strains were
343 generated by transforming the corresponding plasmids via electroporation (56). Each plasmid
344 was transferred into Y. lipolytica YlSR001 via electroporation to generate strains used in this
345 study. The YlSR109, YlSR1001-YlSR1004 strains were confirmed by the respective promoter
346 binding forward primer along with hrGFP_Rev. The YlSR1005 and YlSR1006 strains were
347 confirmed by TEF(-100)_Fwd or P3(-80)_Fwd together with the respective gene binding reverse
348 primer. Escherichia coli TOP10 was used for molecular cloning. Primers used in this study are
349 listed in Supplementary Table S4.
350 Media and culturing conditions
351 Media. For E. coli culture, Luria Bertani medium containing 5 g/L yeast extract, 10 g/L
352 tryptone, and 5 g/L NaCl, 100 mg/L ampicillin as a selection was used. For Y. lipolytica
353 characterization, MpA defined media was used for all experiments. MpA components are as
354 follows: 5 g/L (NH4)SO4, 2 g/L KH2PO4, 0.5 g/L MgSO4, 44 mg/L ZnSO4·7H2O, 79 mg/L
355 CaCL2·2H2O, 0.8 mg/L Biotin, 100mM HEPES buffer, 100mM phosphate buffer (prepared as 0.9M
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356 dibasic, 0.1M monobasic), trace elements (0.4 mg/L ZnSO4·7H2O, 0.04 CuSO4·5H2O, 0.4
357 MnSO4·6H2O, 0.2 mg/L Na2MoO4·2H2O, 0.1 mg/L KI, 0.5 mg/L FeSO4, 0.5 mg/L H3BO3), 380
358 mg/L leucine, 20 g/L glucose and various concentrations of thiamine hydrochloride. Initial media
359 pH was adjusted to 5pH.
360 Culturing. All experiments were conducted in a Kuhner LT-X incubator set to 28°C and
361 250 rpm unless otherwise stated. Fresh colonies were inoculated in 2mL of MpA medium
362 containing 400 µg/L thiamine in 15mL culture tubes overnight. Cultures were centrifuged and
363 resuspended in 2mL of water before transferring 1mL of this suspension into 100mL of MpA
364 containing 5 µg/L thiamine to scale-up cultures for 2 days (Figure 2A). Next, cells were washed
365 once with water and resuspended in 100mL of MpA lacking thiamine for 1 day to eliminate
366 thiamine carry-over (Figure 2A). Finally, cells were washed twice with water before
367 characterization experiments. All experiments were conducted in technical triplicates using
368 500mL baffled flasks unless otherwise stated.
369 Analytical methods
370 Real-time quantitative PCR (rt-PCR). Y. lipolytica, grown in MpA medium using glucose as
371 a carbon source together with either low (0.5 µg/L) and high (500 µg/L) thiamine, was collected
372 at mid-exponential phase (OD 2 ~ 3). Total RNA was purified by using the Qiagen RNeasy mini kit
373 (Cat # 74104, Qiagen Inc, CA, USA), and cDNA was subsequently synthesized by the QuantiTect
374 Reverse Transcription kit (Cat # 205311, Qiagen Inc, CA, USA). To quantify mRNA expression level
375 of genes (e.g., actin (YALI0D08272g), P1, P2, and P3), rt-PCR run was performed using the
376 QuantiTect SYBR Green PCR kit (Cat # 204143, Qiagen Inc, CA, USA) and StepOnePlus™ Real-Time
377 PCR System (Applied Biosystems, CA, USA). Primers used for rt-PCR are listed in Supplementary
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378 Table S4. The gene expression level was investigated after normalizing by the actin house-keeping
379 gene as described elsewhere (23).
380 Promoter characterization with hrGFP. Fresh colonies of Y. lipolytica promoter
381 constructs were grown in 2 mL of MpA medium containing 400 µg/L thiamine overnight. Cultures
382 were washed once with water and transferred into 25mL of MpA containing 5 µg/L thiamine
383 overnight. Finally, cells were washed twice with water before being inoculated in MpA medium
384 with various concentrations of thiamine. Incubation was performed at 400 rpm and 28° using
385 96-well plates and Duetz-system covers (Cat# SMCR1296, Kuhner, Switzerland). Sacrificial
386 samples were collected for fluorescence measurements (excitation at 485 nm and emission at
387 528 nm) using a synergy HT microplate reader.
388 High performance liquid chromatography. Prior to HPLC run, 1 mL of culture medium
389 was filtered using 0.2 m filters. Metabolites, substrates and products were quantified by a
390 Shimadzu HPLC system equipped with UV and RID detectors (Shimadzu Scientific Instruments,
391 Inc., MD, USA) and the Aminex 87H column (Biorad, CA, USA) with 10 mN H2SO4 mobile phase at
392 0.6 mL/min flow rate. The column was maintained at 48 °C (23).
393 Proteomic analysis. Y. lipolytica were grown in biological triplicate in 0 and 400 µg/L
394 thiamine. Samples were collected at two time points during the exponential growth phase and
395 processed for LC-MS/MS analysis. Whole-cell lysates were prepared by bead beating in sodium
396 deoxycholate lysis buffer (4% SDC, 100 mM ammonium bicarbonate, pH 8.0) using 0.15 mM
397 zirconium oxide beads and cell debris cleared by centrifugation (21,000 x g for 10 min). Crude
398 protein concentrations were measured by a NanoDrop OneC (ThermoScientific) using
399 absorbance at 205 nm. Samples were then adjusted to 10 mM dithiothreitol and incubated at
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400 85 °C for 10 min to denature and reduce proteins. Cysteines were alkylated/blocked with 30 mM
401 iodoacetamide followed by 20 min incubation at room temperature in the dark. Proteins (300 µg)
402 were then transferred to a 10-kDa MWCO spin filter (Vivaspin 500, Sartorius) and digested in situ
403 with proteomics-grade trypsin (Pierce) as previously described (57). The tryptic peptide solution
404 was then filtered through the MWCO membrane by centrifugation (12,000 x g for 15 min),
405 adjusted to 1% formic acid to precipitate SDC, and SDC precipitate removed from the peptide
406 solution with water-saturated ethyl acetate. Peptide samples were then concentrated to dryness
407 via SpeedVac, resolubilized in solvent A (5% acetonitrile, 95% water, 0.1% formic acid), and
408 measured by NanoDrop OneC A205 to assess tryptic peptide recovery.
409 Peptide samples were analyzed by automated 1D LC-MS/MS analysis using a Vanquish
410 UHPLC plumbed directly in-line with a Q Exactive Plus mass spectrometer (Thermo Scientific)
411 outfitted with a trapping column coupled to an in-house pulled nanospray emitter. Both the
412 trapping column (100 µm ID) and nanospray emitter (75 µm ID) were packed with 5 µm Kinetex
413 C18 RP resin (Phenomenex) to 10 cm and 30 cm, respectively. For each sample, 3 µg of peptides
414 were loaded, desalted, separated and analyzed across a 210 min organic gradient with the
415 following parameters: sample injection followed by 100% solvent A chase from 0-30 min (load
416 and desalt), linear gradient from 0% to 25% solvent B (70% acetonitrile, 30% water, 0.1% formic
417 acid) from 30-240 min (separation), followed by a ramp to 75% solvent B from 240-250 min
418 (wash), re-equilibration to 100% solvent A from 250-260 min and a hold at 100% solvent A from
419 260-280 min. Eluting peptides were measured and sequenced by data-dependent acquisition on
420 the Q Exactive MS as previously described (57).
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421 MS/MS spectra were searched against the Y. lipolytica proteome concatenated with
422 common protein contaminants using Proteome Discover v.2.2 (ThermoScientific) employing the
423 CharmeRT workflow (58, 59). Peptide spectrum matches (PSM) were required to be fully tryptic
424 with 2 miscleavages; a static modification of 57.0214 Da on cysteine (carbamidomethylated) and
425 a dynamic modification of 15.9949 Da on methionine (oxidized) residues. False-discovery rates,
426 as assessed by matches to decoy sequences, were initially controlled at < 1% at both the PSM-
427 and peptide-levels. FDR-controlled peptides were then quantified by chromatographic area-
428 under-the-curve (AUC), mapped to their respective proteins, and areas summed to estimate
429 protein-level abundance. Protein abundance distributions were then normalized across samples
430 using InfernoRDN (60) and missing values imputed to simulate the MS instrument's limit of
431 detection using Perseus (61). Significant differences in protein abundance were calculated
432 separately for each time point according to the following equation:
WT_00t1,2 − WT_400t1,2 433 Fold change = Variance √0.25 + ∑ ⁄n
434 Here, WT_00 and WT_400 represent log2 normalized abundance of a protein in 0 and 400 µg/L
435 thiamine, respectively. The denominator was used to account for error between replicates.
436 Variance represents the variance of protein abundance between replicates, n represents the
437 number of replicates, and 0.25 is the pseudo variance term (62). Proteins with fold changes >
438 |1| were classified as upregulated or downregulated. Pathway annotations were performed
439 with ClueGo (63) using KEGG (https://www.genome.jp/kegg/) database on proteins that were
440 upregulated or downregulated at both time points.
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441 Bioinformatics. Putative native Y. lipolytica thiamine-regulated promoters were
442 identified by BlastP (64) and orthologs search through the KEGG sequence similarity database
443 (https://www.kegg.jp/kegg/ssdb/). Reference genes used in this study were (i) P. pastoris
444 hydroxymethylpyrimidine phosphate synthase thi11 (PAS_chr4_0065) (65), (ii) S. pombe 4-
445 amino-5-hydroxymethyl-2-methylpyrimidine phosphate synthase nmt1 (NP_588347.1) (55), iii)
446 S. pombe thiamine thiazole synthase nmt2 (NP_596642.1) (66), and iv) S. cerevisiae thiamine
447 thiazole synthase thi4 (NP_011660.1) (67).
448 Lipid quantification. Thiamine-auxotrophic and thiamine-prototrophic strains were
449 cultured in 0 and 400 ug/L thiamine in MpA media in triplicates as outlined previously. Lipid
450 samples were taken from 100 uL samples of culture broth and incubated at room temperature
451 for 15 minutes in the dark after addition of 2 uL of 1 ug/mL BODIPY (cat # D3922, Fisher Scientific)
452 (68). Lipid standards were created by dissolving 100 mg of corn oil in 20mL ethanol and diluted
453 from 1-.1 mg/mL prior to BODIPY staining procedure. Lipids were measured using fluorescence
454 (ex: 485 nm/em: 528 nm) and quantified from corn oil standards. For dry cell weight (DCW)
455 measurement, 1mL of culture broth was sampled from each replicate at each time point.
456 Samples were centrifuged at maximum speed for 3 minutes and supernatant was discarded prior
457 to drying samples at 55°C overnight. DCW was calculated by subtracting the dried cell pellet and
458 tube weight by the empty tube weight. Finally, % lipid accumulation was calculated by dividing
459 the measured lipid mg/mL by DCW mg/mL. Statistical significance was calculated using SigmaPlot
460 14 with one-way analysis of variance (ANOVA) with Holm-Sidak correction between 0 and 400
461 µg/L thiamine for each strain respectively. Symbols: “*”: p-value < 0.05.
462
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463 ACKNOWLEDGEMENTS
464 We would like to acknowledge financial support from the DOE BER Genomic Science
465 Program (DE-SC0019412) and the National Science Foundation (NSF #1511881). The views,
466 opinions, and/or findings contained in this article are those of the authors and should not be
467 interpreted as representing the official views or policies, either expressed or implied, of the
468 funding agencies.
469
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470 FIGURE LEGENDS
471 Figure 1. Metabolic map of thiamine-dependent enzymes (green) in relationship to central
472 (black) and peripheral (blue) pathways. Abbreviations: TPP: thiamine pyrophosphate dependent
473 enzymes, PDH: pyruvate dehydrogenase enzyme complex, KGDH: a-ketoglutarate
474 dehydrogenase, TKL: transketolase, AHAS: acetolactate synthase, BCKDC: branched chain α-
475 ketoacid dehydrogenase, TPP: thiamine pyrophosphate, AAs: amino acids, TCA: citrate (Krebs)
476 cycle, KGA: alpha-ketoglutarate.
477 Figure 2. Growth characterization of the thiamine-auxotrophic Y. lipolytica YlSR001 in 0 (red),
478 0.5 (blue) and 400 (purple) µg/L thiamine. (A) Scheme of thiamine depletion design experiments.
479 (B) Cell growth profiles. (C) Glucose consumption profiles. (D) KGA production profiles. (E)
480 Pyruvate production profiles.
481 Figure 3. Proteomics of the thiamine-auxotrophic Y. lipolytica YLSR001 grown in 0 (red) and 400
482 (purple) µg/L thiamine. (A) Growth profiles and proteomics samples indicated by arrows. (B)
483 Venn diagram representing upregulated and downregulated proteins at both exponential time
484 points. (C) Thiamine-responsive proteomes on metabolic pathways. Bar graphs represent the
485 percentage of proteins upregulated in 0 (red) or 400 (purple) µg/L thiamine for each pathway (D)
486 Electron transport chain and ATPase. (E) Thiamine metabolism of Y. lipolytica. Locus tags: Thi4P:
487 YALI0A09768p, Thi20p: YALI0E04224p, Thi6p: YALI0C15554p, PHO: YALI0A12573p, Thi80p:
488 YALI0E21351p, ADK: YALI0F26521p). Abbreviations: PDH: pyruvate dehydrogenase enzyme
489 complex, KGDH: a-ketoglutarate dehydrogenase, TKL: transketolase, AHAS: acetolactate
490 synthase, BCKDC: branched chain α-ketoacid dehydrogenase, TPP: Thiamine pyrophosphate,
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491 HET-P: hydroxyethylthiazole phosphate, HMP-PP: hydroxymethylpyrimidine pyrophosphate, TP:
492 thiamine monophosphate, TPP: thiamine pyrophosphate, TPPP: thiamine triphosphate.
493 Figure 4. Thiamine-responsive promoter characterization. (A) Chromosomal gene expression of
494 thiamine-responsive genes using rt-PCR. (B) hrGFP protein expression. (C, D) Sensitivity of
495 thiamine-responsive promoters in presence of increasing thiamine concentrations.
496 Figure 5. Expression of pP3-scTHI13 in YlSR1006 restores the de novo thiamine biosynthesis in Y.
497 lipolytica. (A) Cell growth profiles. (B) Glucose consumption profiles. (C) KGA production profiles.
498 (D) Pyruvate production profiles. Growth characterization was conducted in 0 (red), 0.5 (blue)
499 and 400 (purple) µg/L thiamine. Abbreviations: KGA, alpha-ketoglutarate.
500 Figure 6. Lipid production is influenced by thiamine availability. (A) Lipid accumulation profiles
501 for the thiamine-auxotrophic wildtype YlSR001 and thiamine-prototrophic strain YlSR1006 in 0
502 and 400 µg/L thiamine. (B) Lipid accumulation profiles for thiamine-auxotrophic and
503 prototrophic strains in lipid production (C:N = 100) media with 0 and 400 µg/L thiamine.
504 Statistical significance was calculated with one-way analysis of variance (ANOVA) with Holm-
505 Sidak correction between 0 and 400 µg/L thiamine for each strain respectively. Symbols: “*”: p-
506 value < 0.05.
507 Figure 7. A comprehensive model explains detrimental consequences of thiamine deficiency on
508 metabolism and cellular growth of Y. lipolytica.
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509 Figure 1
510
511
512
513
514
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515 Figure 2
516
A 0 µg/L 0.5 µg/L 400 µg/L Inoculum Scale-up Deplete Experiment 400 µg/L 5 µg/L 0 µg/L thiamine B C 12 20
9 no thiamine 15 0.5 g/L thiamine
600nm 6 400 g/L thiamine 10 OD
3 (g/L)Glucose 5
0 0 0 24 48 72 96 0 24 48 72 96 Time (h) Time (h) D E 2.0 5
4 1.5 3 1.0
2 KGA (g/L) KGA
0.5 (g/L)Pyruvate 1
0.0 0 0 24 48 72 96 0 24 48 72 96 517 Time (h) Time (h)
518
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519 Figure 3
520
A C
400 µg/L thiamine 0 µg/L thiamine
B E
D
NADH Cytochrome c Cytochrome c dehydrogenase (I) reductase (III) oxidase (IV) ATPase ATPase ATP synthase (F-type) (V-type) (F-type) Succinate ATPase (V-type) dehydrogenase (II) Downregulated Cytochrome c oxidase (IV) Upregulated Cytochrome c reductase (III) X Succinate dehydrogenase (II) NADH dehydrogenase (I) 0 1 2 3 4 5 521 Number of proteins
522
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523 Figure 4
524
A B 10 5.E+03 0.5 µg/L 1 µg/L 500 µg/L 10 mg/L
8 4.E+03 hrGFP 6 3.E+03
4 2.E+03
2 1.E+03 OD normalized OD normalized
Normalized expression gene Normalized 0 0.E+00 Actin P1 P2 P3 TEF NMT1 P1 P2 P3 Promoters Promoters C D
1.E+04 0.5 µg/L 12 0.5 µg/L 1 µg/L 1 µg/L 8.E+03 2 µg/L 10 2 µg/L 5 µg/L 5 µg/L 10 µg/L 8 10 µg/L 6.E+03 50 µg/L 50 µg/L
600nm 6
4.E+03 OD 4 2.E+03
OD normalized hrGFP hrGFP OD normalized 2
0.E+00 0 0 12 24 36 48 0 12 24 36 48 60 Time (h) Time (h) 525
526
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527 Figure 5
528
A B 12 20
9 15
600nm 6 10
no thiamine OD
0.5 g/L thiamine Glucose (g/L)Glucose 3 400 g/L thiamine 5
0 0 0 24 48 72 96 0 24 48 72 96 Time (h) Time (h) C D 2.5 1.2
2.0 0.9
1.5 0.6
1.0
KGA (g/L) KGA Pyruvate (g/L)Pyruvate 0.3 0.5
0.0 0.0 0 24 48 72 96 0 24 48 72 96 529 Time (h) Time (h)
530
531
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532 Figure 6
533
A B 10 No nitrogen limitation 10 Nitrogen limitation
24h 24h 8 8 48h 48h 72h 72h 6 6
4 4 * * *
* % lipid accumulation % lipid 2 accumulation % lipid 2 * * * * * * * * 0 0 400WT g/L 0 WTg/L 400P3 g/L 0 P3g/L 400WT g/L 0 WTg/L 400P3 g/L 0 P3g/L 400 µg/LWildtype0 µg/L 400 µg/LYlSR10060 µg/L 400 µg/LWildtype0 µg/L 400 µg/LYlSR10060 µg/L 534
535
536
537
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538 Figure 7
539
Consequences of Thiamine Deficiency DNA, RNA, NADPH Antioxidants, Lipids, Ribosome, RNA Purines, Pyrimidines and DNA deficiency Oxidative Stress Ribose-5P Reduced carbon assimilation Xylulose-5P Glycolysis TKL X X X Aromatic AAs Erythrose-4P Folate
Seduheptulose-7P TDL Auxotroph
X TKL
X AHAS X Pyruvate Auxotroph X Branched PDH Acid production chain AAs X X BCKDC X Acetyl-CoA Lipids, Sterols
Deficient lipid NADH production Energy (ATP) Succinyl-CoA TCA KGA deficiency
Electron Transport KGDH Chain Acid production 540
541
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